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Cladosporium fulvum and Dothistroma septosporum Reveal Adaptation to Different Hosts and Lifestyles But
Also Signatures of Common Ancestry
Pierre J. G. M. de Wit, Ate van der Burgt, Bilal Okmen, Ioannis Stergiopoulos, Kamel A. Abd-Elsalam, Andrea L. Aerts, Ali H. Bahkali,
Henriek G. Beenen, Pranav Chettri, Murray P. Cox, et al.
To cite this version:
Pierre J. G. M. de Wit, Ate van der Burgt, Bilal Okmen, Ioannis Stergiopoulos, Kamel A. Abd- Elsalam, et al.. The Genomes of the Fungal Plant Pathogens Cladosporium fulvum and Dothistroma septosporum Reveal Adaptation to Different Hosts and Lifestyles But Also Signatures of Common Ancestry. PLoS Genetics, Public Library of Science, 2012, 8 (11), �10.1371/journal.pgen.1003088�.
�hal-01268262�
Cladosporium fulvum and Dothistroma septosporum Reveal Adaptation to Different Hosts and Lifestyles But Also Signatures of Common Ancestry
Pierre J. G. M. de Wit
1,2*, Ate van der Burgt
1,3, Bilal O ¨ kmen
1, Ioannis Stergiopoulos
1,2,4, Kamel A. Abd- Elsalam
5, Andrea L. Aerts
6, Ali H. Bahkali
7, Henriek G. Beenen
1, Pranav Chettri
8, Murray P. Cox
8, Erwin Datema
9,10, Ronald P. de Vries
11, Braham Dhillon
12, Austen R. Ganley
13, Scott A. Griffiths
1, Yanan Guo
8, Richard C. Hamelin
12, Bernard Henrissat
14, M. Shahjahan Kabir
8, Mansoor Karimi Jashni
1,15, Gert Kema
16, Sylvia Klaubauf
11, Alla Lapidus
6,17, Anthony Levasseur
18, Erika Lindquist
6,
Rahim Mehrabi
1,19, Robin A. Ohm
6, Timothy J. Owen
8,20, Asaf Salamov
6, Arne Schwelm
8,21,
Elio Schijlen
22, Hui Sun
6, Harrold A. van den Burg
1,2,23, Roeland C. H. J. van Ham
9,10, Shuguang Zhang
8,24, Stephen B. Goodwin
25, Igor V. Grigoriev
6, Je´roˆme Collemare
1,2, Rosie E. Bradshaw
8*
1Laboratory of Phytopathology, Wageningen University, Wageningen, The Netherlands,2Centre for Biosystems Genomics, Wageningen, The Netherlands,3Laboratory of Bioinformatics, Wageningen University, Wageningen, The Netherlands,4Department of Plant Pathology, University of California Davis, Davis, California, United States of America,5Agricultural Research Center, Plant Pathology Research Institute, Giza, Egypt,6U.S. Department of Energy Joint Genome Institute, Walnut Creek, California, United States of America,7King Saud University, Riyadh, Saudi Arabia,8Institute of Molecular BioSciences, Massey University, Palmerston North, New Zealand,9Keygene N.V., Wageningen, The Netherlands,10Applied Bioinformatics, Plant Research International, Wageningen, The Netherlands,11CBS–KNAW Fungal Biodiversity Centre, Utrecht, The Netherlands,12Department of Forest Sciences, University of British Columbia, Vancouver, Canada,13Institute of Natural Sciences, Massey University, Albany, New Zealand,14CNRS and Aix-Marseille Universite´, Marseille, France,15Department of Plant Pathology, Tarbiat Modares University, Tehran, Iran,16Department of Bio-Interactions, Plant Research International, Wageningen, The Netherlands,17Cancer Genome Institute, Fox Chase Cancer Center, Philadelphia, Pennsylvania, United States of America,18INRA, Aix-Marseille Universite´, Marseille, France,19Department of Wheat Breeding, Seed and Plant Improvement Institute, Karaj, Iran,20University of Northern British Columbia, Prince George, Canada,21Department of Plant Biology and Forest Genetics, Swedish University of Agricultural Sciences, Uppsala, Sweden, 22Department of Bioscience, Plant Research International, Wageningen, The Netherlands, 23Swammerdam Institute for Life Sciences, University of Amsterdam, Amsterdam, The Netherlands,24Industrial Research Limited, Lower Hutt, New Zealand,25USDA–ARS/Department of Botany and Plant Pathology, Purdue University, West Lafayette, Indiana, United States of America
Abstract
We sequenced and compared the genomes of the Dothideomycete fungal plant pathogens
Cladosporium fulvum (Cfu)(syn.
Passalora fulva) andDothistroma septosporum (Dse)
that are closely related phylogenetically, but have different lifestyles and hosts. Although both fungi grow extracellularly in close contact with host mesophyll cells,
Cfuis a biotroph infecting tomato, while
Dseis a hemibiotroph infecting pine. The genomes of these fungi have a similar set of genes (70% of gene content in both genomes are homologs), but differ significantly in size (Cfu
.61.1-Mb;Dse31.2-Mb), which is mainly due to the difference in repeat content (47.2% in
Cfuversus 3.2% in
Dse). Recent adaptation to different lifestyles and hosts issuggested by diverged sets of genes.
Cfucontains an
a-tomatinase gene that we predict might be required fordetoxification of tomatine, while this gene is absent in
Dse. Many genes encoding secreted proteins are unique to eachspecies and the repeat-rich areas in
Cfuare enriched for these species-specific genes. In contrast, conserved genes suggest common host ancestry. Homologs of
Cfueffector genes, including
Ecp2and
Avr4, are present inDseand induce a Cf-Ecp2- and Cf-4-mediated hypersensitive response, respectively. Strikingly, genes involved in production of the toxin dothistromin, a likely virulence factor for
Dse, are conserved inCfu, but their expression differs markedly with essentially no expression by Cfu in planta. Likewise,Cfuhas a carbohydrate-degrading enzyme catalog that is more similar to that of necrotrophs or hemibiotrophs and a larger pectinolytic gene arsenal than
Dse, but many of these genes are not expressedin plantaor are pseudogenized. Overall, comparison of their genomes suggests that these closely related plant pathogens had a common ancestral host but since adapted to different hosts and lifestyles by a combination of differentiated gene content, pseudogenization, and gene regulation.
Citation:de Wit PJGM, van der Burgt A, O¨ kmen B, Stergiopoulos I, Abd-Elsalam KA, et al. (2012) The Genomes of the Fungal Plant PathogensCladosporium fulvumandDothistroma septosporumReveal Adaptation to Different Hosts and Lifestyles But Also Signatures of Common Ancestry. PLoS Genet 8(11): e1003088.
doi:10.1371/journal.pgen.1003088
Editor:Gregory S. Barsh, Stanford University School of Medicine, United States of America ReceivedMay 4, 2012;AcceptedSeptember 19, 2012;PublishedNovember 29, 2012
Copyright:ß2012 de Wit et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding:This research was supported by Wageningen University, the Royal Netherlands Academy of Arts and Sciences, Centre for Biosystems Genomics, European Research Area-Plant Genomics, Willie Commelin Scholten Foundation, Graduate School of Experimental Plant Sciences, Massey University, the New Zealand Bio-Protection Research Centre, and Royal Society of New Zealand. The work conducted by the U.S. Department of Energy Joint Genome Institute is supported by the Office of Science of the U.S. Department of Energy under contract number DE-AC02-05CH11231. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing Interests:The authors have declared that no competing interests exist.
* E-mail: Pierre.deWit@wur.nl (PJGM de Wit); R.E.Bradshaw@massey.ac.nz (RE Bradshaw)
Introduction
Cladosporium fulvum and Dothistroma septosporum are two related fungal species belonging to the class Dothideomycetes. C. fulvum is a biotrophic pathogen of tomato that has served as a model system for plant-microbe interactions since its first effector gene, Avr9, was cloned in 1991 [1]. It is not related to species in the genus Cladosporium sensu strictu, and has recently been renamed Passalora fulva [2]. However, to be consistent with past literature it will be referred to here as C. fulvum. Phylogenetic analyses based on sequences of the internal transcribed spacer (ITS) region of the ribosomal DNA revealed that C. fulvum is closely related to D.
septosporum and other Dothideomycete fungi such as species of Mycosphaerella isolated from eucalyptus [3]. D. septosporum is an economically important hemibiotrophic pathogen of pine species that is well known for its production of an aflatoxin-like toxin, dothistromin [4]. A taxonomic revision also occurred for this species: prior to 2004 the name Dothistroma pini (syn. D. septosporum syn. D. septospora) was widely used. The revision involved a split into two species: the best-studied and most widespread species was named D. septosporum, and a less common species retained the name of D. pini [5].
The disease caused by C. fulvum, leaf mold of tomato, likely originates from South America, the center of origin of tomato [6].
The first outbreak of the disease was reported in South Carolina, USA, in the late 1800s [7]. Since then, disease outbreaks have occurred worldwide in moderate temperature zones with high relative humidity. The disease was of high economic importance during the first half of the 20
thcentury, but its importance waned after introgression of Cf (for C. fulvum) resistance genes by breeders into tomato cultivars began providing effective control [8].
However, recent outbreaks have been reported in countries where tomato cultivars lacking Cf resistance genes are grown, and in areas where intensive year-round cultivation of resistant tomato plants led to fungal strains overcoming Cf genes [9,10].
In contrast, the foliar forest pathogen D. septosporum (Dorog.) Morelet has a relatively recent history and has been less intensively studied than C. fulvum. D. septosporum infects over 70 species of pine, as well as several minor hosts including some Picea species [11].
During the 1960s–1980s, Dothistroma needle blight (DNB) was largely a problem of Southern hemisphere pine plantations, where primary control was achieved by fungicide applications or planting of resistant species (reviewed in [12]). Since the early 1990s DNB incidence has increased greatly in the Northern hemisphere, with some epidemics causing unprecedented levels of mortality [13,14].
In northwest British Columbia, disease outbreaks are correlated with summer rainfall levels, suggesting that climate change could have unpredictable and severe effects on DNB outbreaks in forests [15].
Infection in both the C. fulvum-tomato and D. septosporum-pine pathosystems starts with conidia that germinate on the leaf surface and produce runner hyphae that enter the host through open stomata. Subsequently, the fungi colonize the apoplastic space between mesophyll cells. In the case of C. fulvum, conidiophores emerge from stomata 10–14 days later producing massive amounts of conidia that can re-infect tomato [16,17,18] (Figure 1A–1D). D.
septosporum produces conidia, several weeks after infection, on conidiomata that erupt through the needle epidermis where they can be spread to other pines by rain splash [19,20] (Figure
1E–1H). Whilst C. fulvum is considered a biotroph, D. septosporum is assumed to be a hemibiotroph based on similarities of its lifecycle to other Dothideomycete fungi.
There is no evidence that C. fulvum has an active sexual cycle, although both mating type idiomorphs occur in its global population [21]. Although D. septosporum also has a predominantly asexual lifestyle, it is known to be sexually active in some parts of the world. The sexual stage Mycosphaerella pini Rostr. (syn Scirrhia pini Funk & Parker) has been reported in some forests in Europe and North America but has not yet been found in other regions, such as South Africa or the United Kingdom, even though both mating types are known to be present [22]. The rare sightings of the sexual stage are due partly to difficulties in identification, but also reflect findings from population studies that show mixed modes of reproduction with a significant clonal component [23,24]. So far, attempts to induce a sexual cycle between opposite mating types of D. septosporum in culture in our laboratory or others (Brown A, unpublished data) have failed. Further research is required to determine environmental conditions conducive to sexual reproduction. The D. septosporum isolate whose genome was sequenced is derived from a clonal population with a single mating type that was introduced into New Zealand in the 1960s [22,25].
The C. fulvum-tomato interaction complies with the gene-for-gene model [2,26]. During infection C. fulvum secretes effector proteins into the apoplast of tomato leaves which function not only as virulence factors, but also as avirulence (Avr) factors when recognized by corresponding tomato Cf resistance proteins. This recognition leads to Cf-mediated resistance that often involves a hypersensitive response (HR) preventing further ingress of the fungus into its host plant tomato [8]. To date many cysteine-rich effectors have been cloned from C. fulvum, including Avr2, Avr4, Avr4E and Avr9, that can trigger Cf-2-, Cf-4-, Cf-4E-, and Cf-9- mediated resistance, respectively, and Ecps (extracellular proteins) like Ecp1, Ecp2, Ecp4, Ecp5 and Ecp6 that trigger Cf-Ecp- mediated resistance [27,28,29]. Specific functions for some C. fulvum effectors have been determined: Avr4 is a chitin-binding protein that protects fungi against the deleterious effects of plant chitinases [30,31], Ecp2 is a virulence factor that occurs in many fungi [32,33]
and Ecp6 sequesters chitin fragments released from fungal cell walls by chitinases during infection thereby dampening their potential to induce pathogen-associated molecular pattern (PAMP)-triggered immunity [28]. Initially, the Avr and Ecp effectors seemed unique to C. fulvum, but in recent years homologs of Avr4, Ecp2 and Ecp6 with functions in virulence have been found in other fungal genomes, including members of the Dothideomycetes [27,28,33].
Whilst most studies of C. fulvum have focused on effectors and their interactions with components in both resistant and suscep- tible plants, studies of D. septosporum have instead focused on dothistromin, a toxin produced by the fungus that accumulates in infected pine needles. Dothistromin is a broad-spectrum toxin with structural resemblance to a precursor of the highly toxic and carcinogenic fungal metabolite, aflatoxin [34]. Although dothis- tromin is not essential for pathogenicity [35], recent observations suggest it to be a virulence factor, affecting lesion size and spore production (Kabir MS and Bradshaw RE, unpublished data).
Some dothistromin biosynthetic genes were identified in D.
septosporum but unexpectedly they were in several mini-clusters
rather than in one co-regulated cluster of genes as reported for
aflatoxin-producing species of Aspergillus [36,37,38]. The similarity
of dothistromin to aflatoxin enabled predictions to be made about other D. septosporum genes involved in dothistromin production [39];
the complete set of dothistromin genes will help us understand the evolution of dothistromin and aflatoxin gene clusters.
Here we report the sequence and comparison of the genomes of C. fulvum and D. septosporum, which have very similar gene contents
but differ significantly in genome size as a result of different repeat contents. We found unexpectedly high levels of similarity in genes previously studied in one or other of these fungi, including those encoding Avr and Ecp effectors of C. fulvum, and dothistromin toxin genes of D. septosporum. Surprisingly, compared to D.
septosporum, C. fulvum has higher numbers of genes normally associated with a necrotrophic or hemibiotrophic lifestyle such as genes for carbohydrate-degrading enzymes and secondary metab- olite biosynthesis. However, in C. fulvum some of these genes were lowly or not expressed in planta and others were pseudogenized.
Other C. fulvum genes that are absent in D. septosporum are putatively involved in virulence on its host plant tomato, such as the
a-tomatinase gene. We suggest that regulation of geneexpression and pseudogenization, in addition to evolution of new genes, are important traits associated with adaptation to different hosts and lifestyles of the two fungi that, however, also retained some signatures of their common ancestral host.
Results/Discussion
C. fulvum and D. septosporum are closely related species with very different genome sizes
The 30.2-Mb genome of D. septosporum (http://genome.jgi.doe.
gov/Dotse1/Dotse1.home.html; GenBank AIEN00000000) was sequenced at 34-fold coverage (Table S1) and then assembled into 20 scaffolds (.2-kb), 14 of which were 407-kb or larger, have telomere sequences at one or both ends (Table S2) and mostly match chromosome sizes estimated from pulsed-field gel electro- phoresis [36]. The six smallest scaffolds ranged from 2.3- to 5.2-kb in size so are not significant parts of the genome. The excellent
Figure 1. Symptoms caused byCladosporium fulvumandDothistroma septosporumon their host plants. (A–D) Disease symptoms of Cladosporium fulvumon tomato. A)C. fulvumsporulating on the lower side of a tomato (Solanum lycopersicum) leaf two weeks post inoculation; B) Close-up ofC. fulvumsporulating on the lower side of a single leaflet two weeks post inoculation; C) Runner hyphae ofC. fulvum(GFP-transgenic strain) at the surface of the leaf; two of them are penetrating a stoma of tomato four days post inoculation; D) Conidiophores ofC. fulvum(GFP- transgenic strain) emerging from a stoma at 10 days post inoculation. (E–H) Disease symptoms ofDothistroma septosporumon pine. E) Mortality of mature lodgepole pines (Pinus contortavar.latifolia) in northwest British Columbia, Canada caused byD. septosporum; F) Red band lesions with conidiomata onPinus radiataneedles; G) Penetration of hypha into stoma ofP. radiataneedle 4 weeks post inoculation; H) Eruption of conidiospores through epidermis of pine needle 8 weeks post inoculation.
doi:10.1371/journal.pgen.1003088.g001
Author Summary
We compared the genomes of two closely related pathogens with very different lifestyles and hosts:
C.fulvum
(Cfu), a biotroph of tomato, and
D. septosporum(Dse), a hemibiotroph of pine. Some differences in gene
content were identified that can be directly related to their
different hosts, such as the presence of a gene involved in
degradation of a tomato saponin only in
Cfu. However, ingeneral the two species share a surprisingly large
proportion of genes.
Dsehas functional homologs of
Cfueffector genes, while
Cfuhas genes for biosynthesis of
dothistromin, a toxin probably associated with virulence in
Dse.Cfualso has an unexpectedly large content of genes
for biosynthesis of other secondary metabolites and
degradation of plant cell walls compared to
Dse, contrast-ing with its host preference and lifestyle. However, many
of these genes were not expressed
in plantaor were
pseudogenized. These results suggest that evolving
species may retain genetic signatures of the host and
lifestyle preferences of their ancestor and that evolution of
new genes, gene regulation, and pseudogenization are
important factors in adaptation.
assembly of the D. septosporum genome was facilitated by its very low repeat content of only 3.2% (Table 1; Table 2; Protocol S1). In contrast, the repeat-rich genome of C. fulvum (http://genome.jgi- psf.org/Clafu1/Clafu1.home.html; GenBank number AMRR00000000) was very difficult to assemble. Fourteen 2-kb paired-end or shotgun 454 sequencing runs for C. fulvum resulted in a 21-fold coverage of the 61.1-Mb assembly in 2664 scaffolds
.2-kb (Table 1) with a total repeat content of 47.2% (Table 2).The sequencing strategy was initially based on the assumption of a genome size of around 40-Mb, but soon it appeared that the C.
fulvum genome was much larger due to the high repeat content.
Problems with the assembly are not caused by the sequencing coverage of C. fulvum because it is estimated to be sufficiently high for good coverage of the gene-encoding areas. Instead, they are a consequence of its high repeat content. An estimated additional 26-Mb of C. fulvum DNA reads could not be assembled as they were predominantly repeat sequences (Figure 2). In the remainder of the manuscript we refer to chromosomes (1 to 14) for D.
septosporum and scaffolds for C. fulvum. Summary statistics for the two genomes are shown in Table 1 and at the Joint Genome Institute (JGI) Genome portal (jgi.doe.gov/fungi) [40]. The C.
fulvum and D. septosporum genomes are predicted to encode approximately 14 and 12.5 thousand gene models, respectively.
Nevertheless, the C. fulvum and D. septosporum genomes share more than 6,000 homologous gene models with at least 80% similarity at the predicted amino acid level, whereas this number drops to 3,000 gene models this similar when comparing C. fulvum or D.
septosporum with other closely related Dothideomycete species such as Mycosphaerella graminicola and M. fijiensis (Figure 2, Figure S1).
Similarly, most introner-like element clusters found in C. fulvum
and D. septosporum are closely related, more than to elements in other Dothideomycetes [41].
Phylogenetic analysis of C. fulvum and D. septosporum genomes in the context of nine other Dothideomycetes [42] confirms that these two species are the most closely related of the sampled species (Figure 2), as was inferred earlier from ITS [3] and mating type sequences [21]. This gives us two very closely related genomes with drastically different genome sizes mostly due to the greatly increased repeat content of C. fulvum.
C. fulvum and D. septosporum differ in content and classes of repeats that are affected by repeat-induced point mutation
The massive increase in repetitive elements in C. fulvum might result from expansion of one or more repeat families that are also present in D. septosporum. Therefore, we classified the different repeat families in D. septosporum and compared them with those in C. fulvum. This revealed that some of the repetitive element families present in D. septosporum have expanded in C. fulvum (Table 2). This is most remarkable for the Class I retrotransposons which comprise over 90% of the repetitive fraction in C. fulvum and together account for over 26-Mb of the assembled genome.
Retrotransposons are also highly abundant in the large repeat-rich genome of the hemibiotrophic sexual pathogen Mycosphaerella fijiensis (Dhillon B, Goodwin SB and Kema GHJ, unpublished data). Both Copia and Gypsy LTR retroelements are expanded in C. fulvum compared to the D. septosporum genome, whereas LINEs are detected only in C. fulvum (Table 2). Some other fungal species that are closely related to each other, but have a different lifestyle,
Figure 2. Species phylogeny, amino acid similarity, and repeat content.A) Maximum likelihood phylogenetic tree based on 51 conserved protein families showing evolutionary relationships ofCladosporium fulvumandDothistroma septosporum. Branch lengths are indicated by the bar (substitutions/site); bootstrap values are shown as percentage. B) Genome-wide amino acid similarity of homologous proteins betweenC. fulvumand other sequenced fungal species. A pair of proteins is only reported as homologous when the predicted similarity (blastp) spans at least 70% of their lengths and their length difference is at most 20%. Axis indicates number of homologous proteins. Bar shading indicates similarity: red, 91–100%;
orange, 81–90%; light green, 71–80%; medium green, 61–70%; turquoise, 51–60%; light blue, 41–50%; dark blue, 31–40%; and purple, 0–30%.
Homologous proteins with high amino acid similarity are likely orthologs, whereas for those with lower similarity this relation cannot be inferred. C) Repeat content ofC. fulvum,D. septosporumand other sequenced fungal species. Bar shading indicates repeat class: red, unique non-repeat regions;
brown, repeat elements; green, continuous tracts of N characters; blue, duplicated regions; and grey, poorly assembled regions (C. fulvumonly). Axis indicates number of nucleotides (Mb).
doi:10.1371/journal.pgen.1003088.g002
also differ in repeat content, such as the Leotiomycetes of which Botrytis cinerea (,1% repeats) and Sclerotinia sclerotiorum (7% repeats) are necrotrophs, while Blumeria graminis f. sp. hordei (64% repeats) is an obligate biotroph [43,44]. The latter species is particularly enriched in Class I elements and one of several biotrophs that show expansion of genome size associated with high repeat content [44,45].
In contrast to the retroelements, Class II DNA transposons comprise only a small percentage (4.7%) of the overall repetitive elements in C. fulvum, but 46.2% of the repeats in D. septosporum, although they make up only a small portion of the genome overall.
Interestingly, helitron-like DNA transposons comprise 40% of all repeats in D. septosporum and are 25.8-fold higher in terms of sequence coverage than in C. fulvum, whereas the DDE-1, hAT, and MuDR_A_B DNA transposons present in C. fulvum are not present in D. septosporum. Helitrons are transposons that replicate by a rolling-circle mechanism and are found in a wide range of eukaryotes, including the white rot fungus Phanerochaete chrysosporium [46], and are thought to have a role in genome evolution [47].
Helitron-like repeats are particularly abundant on D. septosporum chromosomes 3, 6 and 11 (Figure 3) and usually occur in clusters, sometimes along with other types of repetitive elements.
The organization of repeats in D. septosporum is striking in that for the majority of the chromosomes, most repeats are localized into just one or two large regions containing a mixture of repeat element types (Figure 3), although other small repeat clusters also occur. In many eukaryotes, centromeres are characterized by repetitive DNA [48], and therefore we propose that some of the larger complex repeat regions are centromeres, in line with similar suggestions made for other fungal genomes [49], although experimental confirmation is required. The absence of any repeat cluster from chromosome 14, along with the observation that it harbors only one telomere, suggests that it is a chromosome fragment.
Repeats in fungi are affected by repeat-induced point mutation, also referred to as RIP, a defense mechanism employed by fungi to suppress transposable element activity that was first described in Neurospora crassa [50]. RIP is a process by which DNA accumulates G:C to A:T transition mutations. It occurs during the sexual stage in haploid nuclei after fertilization but prior to meiotic DNA replication. Clear evidence of RIP was found in both the C. fulvum and D. septosporum genomes (Table 3) and is mainly confined to repeat-rich regions. In total 25.9-Mb were RIP’d in C. fulvum and 1.1-Mb in D. septosporum, which represent 42.4% and 3.7% of their genomes, respectively. RIP occurred mainly on large repeated sequences ($500 nucleotides) that represent 97.2% of all repeats in C. fulvum and 98.0% in D. septosporum (Table 3). The high rate of RIP in repeat regions is in the same range as that seen in other Dothideomycetes such as S. nodorum (97.2%; Table S3) [42,51].
Although RIP is present at high levels in C. fulvum, we propose that it has not been able to prevent transposon expansion possibly due to very rare sexual activity.
Of the RIP’d loci, C. fulvum has almost none (0.5%) and D.
septosporum little (16.9%) outside the main classified repeat regions.
This is different from N. crassa (Table S3), where 35.2% of all RIP’d loci are predicted to be non-repeat-associated. For N. crassa it has been shown that even single gene duplication events are prey to the RIP machinery, thereby exemplifying its efficiency and sensitivity [50]. Clearly such sensitivity is not applicable to C.
fulvum and D. septosporum, nor for three other studied Dothideo- mycetes (Table S3). In the Dothideomycete phytopathogenic fungus Leptosphaeria maculans, RIP slippage is found in regions adjacent to repetitive elements. In that species RIP has occurred in genes encoding small secreted proteins, such as the effector genes AvrLm6 [52] and AvrLm1 [53] that are located in repeat-rich regions of the genome [54]; mutations in these genes caused by the RIP process enabled the fungus to overcome Lm6 and Lm1- mediated resistance, respectively. However, we found no evidence of RIP slippage into the known effector genes of C. fulvum and related effector genes in D. septosporum.
The C. fulvum and D. septosporum genomes show extensive intrachromosomal rearrangements
One way to assist the assembly of a fragmented genome is to use synteny with a well-assembled genome of a closely related species to order the scaffolds [55]. We attempted to use the D. septosporum genome to improve the C. fulvum assembly in this way. However, although it was possible to map C. fulvum scaffolds onto the assembled D. septosporum genome (Figure S2A), individual C. fulvum scaffolds are not collinear along their length, but have only short blocks of synteny to different parts of the D. septosporum chromosomes. The syntenic regions of the C. fulvum and D.
septosporum genomes are associated with just 461 of the C. fulvum scaffolds (Table 4). In contrast, the remaining
.4,000C. fulvum scaffolds are non-syntenic. A more detailed analysis with the ten largest C. fulvum scaffolds (two are shown in Figure S2B) revealed that they each match primarily to only one D. septosporum chromosome, suggesting predominantly intrachromosomal rear- rangements (mesosynteny), as described for other Dothideomycete fungi [42,56] (Condon B et al., unpublished data). As found in other fungi [43,57] non-syntenic regions are repeat-rich; for C.
fulvum 79.7% of the repeat sequences are present in non-syntenic regions (Table 4).
Non-syntenic, repeat-rich regions are enriched in genes encoding secreted proteins
Secreted proteins are important for communication of plant- pathogenic fungi with their hosts. They comprise not only enzymes required for penetration and growth on plant cell walls, but also proteins needed to compromize the basal defence system of plants by either suppressing or attacking it, as has been reported for several fungal effector proteins [58]. The percentage of
Table 1.C. fulvumand
D. septosporumgenome statistics.
Species
Genome
assemblysize (Mb)
Number of predicted gene
models Sequencing coverage depth
Number of scaffoldsa
Scaffold L50/
N50b(Mb)
% GC content
C. fulvum 61.1 14,127 21 2,664.2 kb 279.50 kb 250/0.06 48.8
D. septosporum 30.2 12,580 34 20.2 kb 14.50 kb 5.0/2.6 53.1
aFor details see Protocol S1.
bL50 is defined as the smallest number of scaffolds that make up 50% of the genome; N50 is defined as the size (Mb) of the smallest of the L50 scaffolds.
doi:10.1371/journal.pgen.1003088.t001
Table2.RepetitiveelementsintheC.fulvumandD.septosporumgenomes. C.fulvumD.septosporum RepeatclassRepeattypeTotalbasescoveredPercentofgenomeaPercentofrepetitive fractionaTotalbases coveredPercentof genomePercentofrepetitive fraction ClassITy1-CopiaLTR3,208,3055.311.143,5980.14.5 RetrotransposonsTy3-GypsyLTR13,557,45722.247.0178,8600.618.6 Misc.LTR000167,8930.617.5 LINE9,464,47615.532.8000 Sub-total26,230,23842.990.9390,3511.340.60 ClassIIDDE-1960,3731.63.3000 DNAtransposonshAT144,7650.20.5000 Helitron14,9010.020.1384,2331.340.0 Mariner96,1240.20.357,6460.26.0 MITE98,0470.20.32,1650.010.2 MuDR_A_B50,8990.10.2000 Sub-total1,365,1092.24.7444,0441.546.2 UnclassifiedUnclassified1,255,5292.14.4127,0270.413.2 TOTAL28,850,87647.2961,4223.2 aNumbersrefertorepeatspresentinassembledgenome. doi:10.1371/journal.pgen.1003088.t002
proteins predicted to be secreted is similar for both C. fulvum (8.5%) and D. septosporum (7.2%), and in the same range as that predicted for other Dothideomycete fungi such as M. graminicola (9.1%) and S. nodorum (10.8%) [40,42,51,59].
Genes encoding secreted proteins including effectors are subject to evolutionary selection pressure imposed by environmental and host plant factors [58], and they often show a high level of diversification. Repeat-rich, gene-poor regions have been proposed to contain genes involved in adaptation to new host plants. For example, in some Phytophthora species and in L. maculans significantly higher proportions of in planta-induced species-specific effector genes encoding secreted proteins are found in repeat-rich compared to repeat-poor regions [50,59] and in pathogenic strains of Pyrenophora tritici-repentis transposable elements are associated with effector diversification (Manning V, Ciuffetti L, unpublished data). We hypothesized that we would find more genes encoding secreted proteins in repeat-rich regions that are less syntenic between the C.
fulvum and D. septosporum genomes than in repeat-poor syntenic regions. We therefore compared the number of genes and their similarity at the nucleotide and protein levels in syntenic and non- syntenic regions of these two genomes (Table 5) using C. fulvum as the reference sequence due to its higher overall content of repeat elements in non-syntenic regions. The regions syntenic between C.
fulvum and D. septosporum, representing 22.3-Mb of the C. fulvum genome, contain 70% of all predicted genes whereas 30% of the genes are located in the non-syntenic repeat-rich regions represent- ing 38.8-Mb of the C. fulvum genome (Table 5). The syntenic regions contain most of the homologous genes that encode proteins with the highest level of conservation between the two genomes, whereas the proteins encoded by genes located in the non-syntenic, repeat-rich regions are less conserved. In syntenic regions, 89.9% of gene models have a bi-directional best BLAST hit (BDBH) to a D.
septosporum gene model, with a mean predicted amino acid similarity of 85.2%, compared to non-syntenic with only 51.7% of gene models with BDBH and 65.1% amino acid similarity (Table 5). As expected, we found the repeat-rich, non-syntenic regions to have higher proportions of gene models encoding secreted proteins
(10.4%, with a mean predicted amino acid similarity of 60.7%) and small secreted cysteine-rich proteins (2.8%) than in syntenic regions (7.6%, with a mean amino acid similarity of 81.1%, and 1.5% respectively) (Table 5), as has been reported for L. maculans [54].
C. fulvum and D. septosporum share functional effectors Some C. fulvum effector homologs have previously been reported to occur in other Dothideomycete species including M. fijiensis, M.
graminicola, and several Cercospora species [33], but in the D.
septosporum genome we found the highest number of C. fulvum effector homologs discovered to date, including Avr4, Ecp2-1, Ecp2- 2, Ecp2-3, Ecp4, Ecp5 and Ecp6. Of those, Avr4, Ecp2-1 and Ecp6 are core effectors [33] and show the highest identity (51.7%, 59.8% and 68.6% amino acid identity, respectively) with those present in C. fulvum, whilst Ecp4 and Ecp5 are pseudogenized. We were interested to know whether the D. septosporum effectors would be functional in triggering a Cf-mediated hypersensitive response (HR). Therefore, we inoculated plants of tomato cultivar Moneymaker (MM) carrying the Cf-Ecp2 resistance trait with Agrobacterium tumefaciens expressing potato virus X (PVX) containing D. septosporum Ecp2-1 and used PVX-containing C. fulvum Ecp2-1 as a positive control. D. septosporum Ecp2-1 triggered a Cf-Ecp2-1- mediated HR (Figure 4A), whilst MM tomato plants lacking Cf- Ecp2 did not show any HR when inoculated with PVX containing Ds-Ecp2-1 (results not shown). We also showed that the D.
septosporum homolog of C. fulvum Avr4 is functional in triggering a Cf-4-mediated HR in Nicotiana benthamiana, as determined with an Agrobacterium transient transformation assay (Figure 4B). This is remarkable because D. septosporum infects a gymnosperm which is only distantly related to tomato, but apparently produces effectors that can be recognized by tomato Cf resistance proteins. It would be interesting to examine whether gymnosperms carry functional homologs of the well-studied Cf tomato resistance gene homologs [33,60] or other major R genes that could confer resistance to D.
septosporum. Major R genes have been shown to be involved in resistance of some pine species to Cronartium spp. rust pathogens
Figure 3. Organization of repeats and pathogenicity-related genes in the Dothistroma septosporum genome. The fourteen chromosomes from theD. septosporumgenome assembly are shown as GC (dark grey line) and AT (pale grey line) content (%) plots made from a 500-bp sliding window using Geneious (www.geneious.com). All chromosomes have telomere sequence at both ends except chromosomes 2, 11 and 14 which have telomere sequences only at the left end as shown in the figure. Chromosome 1 has been split into two parts in the figure (L, R) because of its length, and the GC/AT content scale is shown beside the right arm of this chromosome. The positions of putativeAvrandEcpeffector, secondary metabolite, dothistromin biosynthesis, and mating type genes are shown above the GC/AT content plot, while the positions of repeats (.200-bp) are shown below the plot. Color-coding of the gene and repeat types is indicated in the legend. Most chromosomes have repeat clusters at one or two sites that coincide with regions of high AT content. The chromosome sizes are to scale, as indicated by the vertical pale grey lines, with the values (in kb) shown at the bottom; neither the genes nor the repeats are drawn to scale.doi:10.1371/journal.pgen.1003088.g003
Table 3.
Occurrence of Repeat-Induced Point Mutation (RIP) signatures and repeats in
C. fulvumand
D. septosporum.Cladosporium fulvum Dothistroma septosporum
Bases (kb) Locia Bases (kb) Locia
RIP’d sequence in genome 25,882 (42.4%)b 5447 1,114 (3.7%)b 65
Repeat sequence$500 nt in genomec 27,170 (44.5%)b 7101 798 (2.6%)b 133
Repeat sequence$500 nt with RIP signatured 26,397 (97.2%)e 6506 (91.6%)e 782 (98.0%)e 114 (85.7%)e
aNumber of loci, defined as consecutive blocks of sequence assigned as repeats or RIP’d regions.
bPercentage of the genome is indicated in brackets.
cOnly classified repeats (as shown in Table 2) were considered.
dRepeated sequence$500 nt that (at least partially) overlaps with RIP’d sequence.
ePercentage of classified repeats is indicated in brackets.
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[61,62] and are thought to function in a gene-for-gene manner [63].
In C. fulvum, adaptation to resistant tomato cultivars is sometimes associated with deletion of effector genes [64]. Presence of repeats or location near a telomere can cause repeat-associated gene deletion [65]. We analyzed the location of all cloned C. fulvum effector genes in its genome. Many scaffolds containing an effector gene are very small (Figure 5), suggesting that they are surrounded by large repeats hampering assembly into larger scaffolds. The location of the C. fulvum effectors is shown in Figure 5 and the types of flanking repeats are detailed in Table S4. The well-character- ized effector gene Avr9 is located on a very small (20-kb) scaffold (Figure 5) and is likely flanked on both sides by repeats; on one side there are 11-kb of repeats on the scaffold and on the other side probably also repeats just outside the region shown that prevented further scaffold assembly. This suggests that the absolute correlation found between deletion of the Avr9 gene in C. fulvum and overcoming Cf-9-mediated resistance [64] is most likely due to the close proximity of Avr9 to large, unstable repeat regions. As well as causing deletions, transposons can contribute to genome plasticity by mutation due to transposition into coding sequences.
During co-evolution, transposons have inserted into effector genes causing their inactivation and overcoming Cf-mediated resistance in C. fulvum, as has been reported for inactivation of both Avr2 [64]
and Avr4E [66]. The C. fulvum homologous effector genes present in D. septosporum are also often in close proximity to repeat-rich areas that may represent centromeres (Figure 3), but the biological significance of this is not yet clear.
Pseudogenization of two D. septosporum effector genes, Ecp4 and Ecp5, homologous to those reported for C. fulvum [67], could point to host adaptation in the DNB fungus at the pine genus, species or cultivar level. Future population analysis of both fungal strains and host genotypes will reveal the mechanism behind this phenome- non.
New hydrophobin genes in C. fulvum
Another class of well-studied C. fulvum small cysteine-rich secreted proteins is the hydrophobins. These amphipathic proteins are implicated in developmental processes in filamentous fungi and are localized on the outer surface of fungal cell walls [68].
They are divided into class I and class II hydrophobins based on sequence differences that also correlate with their different solubility [68].
Six hydrophobin genes (Hcf-1 to Hcf-6) had previously been identified from C. fulvum [66,67]. We identified five additional hydrophobin genes in the C. fulvum genome [two class I (Cf187601 and Cf189770) and three class II (Cf197052, Cf188363 and Cf183780)] (Figure S3), which makes C. fulvum the Ascomycete
Table 4.Syntenic and non-syntenic regions between
C. fulvumand
D. septosporumare unevenly distributed over the
C. fulvumscaffolds.
Feature Syntenic Non-syntenic Total Syntenic % Non-syntenic %
Number of scaffolds 461 4,404 4,865 9.5 90.5
Number of repeats 2,090a 6,234 8,324 25.1 74.9
Mb in scaffolds 37.4b 23.7 61.1 61.2 38.8
Mb in repeats 5.6c 21.9 27.5 20.3 79.7
Mb in whole genome 22.3b 38.8 61.1 36.5 63.5
aNumber of repeat regions on syntenic vs. non-syntenic scaffolds.
bA syntenic scaffold is one that contains at least a single syntenic block, but may not be syntenic along its entire length. Total syntenic scaffold size (37.4-Mb) is therefore larger than total syntenic size in whole genome (22.3-Mb).
cSummed repeat length on syntenicversusnon-syntenic scaffolds.
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Table 5.
Location of gene models of
C. fulvumin regions syntenic or non-syntenic with the
D. septosporumgenome.
Number of gene modelsa Percentage of gene modelsb
Total Syntenic Non-syntenic Syntenic Non-syntenic
All proteinsc 14,127 9,890 4,237 70.0 30.0
BDBHd 11,092 8,900 2,192 89.9g 51.7g
Secreted proteinse 1,195 754 441 7.6h 10.4h
Secreted Cys-rich proteinsf 271 151 120 1.5 2.8
aValues are numbers of gene models located in regions of theC. fulvumgenome syntenic or non-syntenic with theD. septosporumgenome as described in Materials and Methods.
bFor all proteins the percentage of gene models represents the fraction of all gene models present in theC. fulvumgenome; for other categories (BDBH, secreted proteins, secreted Cys-rich proteins) the percentage of gene models represents the fraction of gene models present in syntenic and non-syntenic regions.
cAll proteins encoded by predicted gene models in theC. fulvumgenome.
dBi-directional best BLAST hit betweenC. fulvumandD. septosporumproteins with at least 50% (global) pairwise amino acid similarity and at least 60% coverage by overlap-corrected blastp HSPs.
eGene models predicted to encode secreted proteins.
fSecreted small cysteine-rich proteins contain less than 300 amino acids of which at least four are cysteines.
gThe mean amino acid similarities of all protein gene models in syntenic regions and non-syntenic regions are 85.2% and 65.1%, respectively.
hThe mean amino acid similarities of secreted protein gene models in syntenic regions and non-syntenic regions are 81.1% and 60.7%, respectively.
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species with the largest number of hydrophobin genes reported so far. In the D. septosporum genome only four hydrophobin genes were found, one of which (Ds75009) is predicted to encode a class II hydrophobin and was highly expressed both in culture and in planta. Based on EST data the 11 C. fulvum hydrophobin genes show a range of different expression patterns. Of the six class I C.
fulvum hydrophobins, two were only expressed in culture [Cf184635 (Hcf-2) and Cf189850 (Hcf-4)], three were expressed both in culture and in planta [Cf189770, Cf187601 and Cf193176 (Hcf-1)], and one was not expressed in culture or in planta [Cf184193 (Hcf-3)]. Three of the class II C. fulvum hydrophobins were only expressed in culture [Cf197052, Cf188363 and Cf193013 (Hcf-5)], whilst Cf193331 (Hcf-6) and Cf183780 were expressed neither in culture nor in planta. None of the C. fulvum hydrophobin genes were expressed in planta only. It has been proposed that hydrophobins may act as ‘stealth’ factors, prevent- ing the invading fungus from detection by its host plant [69] or protecting it against deleterious effects of plant chitinases and
b-1,3glucanases as reported for C. fulvum [70]. Early functional studies focused on the hydrophobin genes Hcf-1 (Cf193176) and Hcf-2 (Cf184635). Knocking down expression of Hcf-1, Hcf-2, or both genes by homology-dependent gene silencing did not compromise virulence [71,72]; a similar result was reported for knock-down mutants of class I Hcf-3 and Hcf-4 and class II Hcf-6 genes [73]. A phylogenetic tree (Figure S3) shows that the four class I genes (Hcf- 1 to Hcf-4) are paralogs, suggesting functional redundancy that might explain the lack of a phenotype; functional redundancy may also exist between different classes. It would be interesting to examine the role in virulence of the two most similar hydrophobin class I and class II genes of C. fulvum and D. septosporum (Cf 189770/
Ds67650 and Cf197052/Ds75009, respectively) either by knock- out or knock-down strategies.
Carbohydrate active enzyme gene and expression profiles reflect adaptation to different host plants
Because C. fulvum and D. septosporum have very different plant hosts and pathogenic lifestyles, we expected that their capacity to
degrade carbohydrates would also differ and that this might be reflected in their gene complements and expression profiles. We compared numbers of genes predicted to encode carbohydrate- active enzymes (CAZymes) [74] in these two fungi to those in other fungi representative of different lifestyles. As seen for grouped families of CAZyme genes in Table 6 (e.g., GH family of glycoside hydrolases), both C. fulvum and D. septosporum have gene numbers in the same range as hemibiotrophic and necrotrophic fungi, and many more than the obligate biotroph B. graminis f. sp. hordei.
Despite this, both C. fulvum and D. septosporum have fewer predicted cellulolytic enzyme genes (e.g., GH6, GH7) as well as fewer genes classified in carbohydrate binding module gene families (e.g., CBM1) than most of the other fungi shown except for M.
graminicola (Table 6, Table S5). The reduced number of predicted genes for cell wall-degrading enzymes in M. graminicola was hypothesized to represent an adaptation to avoid host defenses during stealth pathogenicity [59], which also may apply to C.
fulvum and D. septosporum. However, it is known that even a small number of genes can enable high levels of enzymatic activity, as has been shown for the strongly cellulolytic fungus Trichoderma reesei [75].
Next we focused on CAZyme gene families that appear to differ in gene number between C. fulvum and D. septosporum. Because small differences in gene number could be due to mis-annotation, only families that differed by two or more genes were considered and examples of these are shown in Table 6 (full data in Table S5).
Potentially interesting is the expansion of genes associated with pectin degradation in C. fulvum. For example, in the GH28 family that includes many pectinolytic enzymes, C. fulvum has 15 genes whilst D. septosporum has only four. A higher pectinolytic activity in C. fulvum is concordant with the higher pectin content of its host, tomato, compared to the pine host of D. septosporum [76,77], but larger numbers of genes encoding pectin-degrading enzymes have generally been associated with a necrotrophic rather than a biotrophic lifestyle in fungi [78]. High pectinolytic activity is observed in fungi such as Botrytis cinerea [79,80] that invades soft, pectin-rich plant tissues causing a water-soaked appearance of the
Figure 4. Recognition ofDothistroma septosporumeffectors by tomato Cf receptors.A)DsEcp2-1, theD. septosporumortholog ofCfEcp2-1, was cloned intopSfinx. Tomato plants were inoculated withAgrobacterium tumefacienstransformants expressingpSfinx::DsEcp2-1. A hypersensitive response (HR) was induced in the tomato line carrying theCf-Ecp2resistance gene (MM-Cf-Ecp2). Empty vector was used as a negative control and caused only mosaic symptoms. Pictures were taken at four weeks post inoculation. B) TheC. fulvumavirulence geneAvr4(CfAvr4) and its ortholog in D. septosporum (DsAvr4)were heterologously expressed inCf-4transgenicNicotiana benthamianausing theA. tumefacienstransient transformation assay (ATTA). Expression ofCfAvr4andDsAvr4results in an HR demonstrating that the tomato Cf-4 receptor recognizes DsAvr4. Picture was taken at six days post inoculation.doi:10.1371/journal.pgen.1003088.g004
infected tissues [43]. However, during colonization of tomato leaves by C. fulvum this type of symptom is never observed [79,80].
Instead of contributing to the destruction of host cell walls, the C.
fulvum pectinolytic enzymes may facilitate local modification of primary cell walls of mesophyll cells allowing the fungus to thrive in the apoplast of tomato leaves, as suggested for the ectomycor- rhizal fungus Laccaria bicolor that thrives on plant roots [81].
Although C. fulvum has a large arsenal of pectinolytic genes compared to D. septosporum, not all of them appear to be functional.
For example, two of the six GH78 and one of the two GH88 pectinolytic genes are pseudogenized in C. fulvum, whilst the corresponding D. septosporum families do not contain pseudogenes.
Another constraint to function is that gene expression appears to be tightly regulated. As shown in Table 6, none of the 15 C. fulvum GH28 genes appear to be expressed in planta, whilst all four D.
septosporum GH28 genes are expressed. Indeed in all gene families with predicted pectinolytic function shown in Table 6 (GH28, GH78, GH88, GH95, PL1, PL3), expression in planta was only detected for 2 of the 31 C. fulvum genes, whilst all 6 genes in these pectinolytic gene families were expressed in D. septosporum. It is possible that C. fulvum pectinases are only expressed very locally to modulate complex primary cell wall structures. The location and
accessibility of pectin structures embedded in the cell wall is an important consideration for its enzymatic degradation. For instance, the Basidiomycete Schizophyllum commune grows predom- inantly on beech and birch wood which is poor in pectin [82].
However, the pectin in these cell walls is concentrated around the bored pits that are used by S. commune to enter the wood, explaining why this fungus contains a higher number of pectinase genes than would be expected based on the overall host pectin content. Differences in pectinolytic gene content and expression between C. fulvum and D. septosporum may therefore be related to their different strategies of host invasion and subsequent coloni- zation.
In addition to increased numbers of pectinolytic genes compared to D. septosporum, C. fulvum has more genes for enzymes that degrade hemicelluloses (e.g., families GH31, GH35 and GH39) [83] and hemicellulose-pectin complexes (GH43) (Table 6).
It also contains 11 genes (compared to 4 in D. septosporum) encoding CE5 enzymes; these include cutinases that are required for early recognition and colonization of the host by fungal pathogens [84,85]. The presence of so many genes encoding enzymes for plant cell wall and cuticle degradation in a biotrophic fungus like C. fulvum that enters its host via stomata is unexpected. However,
Figure 5. Repetitive regions flanking known effectors ofCladosporium fulvum.Scaffolds harboring sequencedC. fulvumeffector genes with flanking repeats. Repeat regions longer than 200-bp are shown, with different types indicated in different color code. Red arrows depict the effector genes and sizes are in kb. The sizes of scaffolds range from 8 to 213-kb but some are shortened to fit the figure due to differences in size.doi:10.1371/journal.pgen.1003088.g005
the number of cutinase genes, and other secreted lipase genes is particularly low in the D. septosporum genome compared to other Dothideomycetes, a feature shared with the other tree pathogens Mycopshaerella populorum and M. populicola [42].
Overall our comparison shows a similar complement of CAZy genes between C. fulvum and D. septosporum, but an increased number of particular CAZyme families in C. fulvum including genes encoding pectin- and hemicellulose-degrading enzymes. However, a large proportion of genes in the C. fulvum CAZyme families lack expression in planta and some genes are pseudogenized.
C. fulvum and D. septosporum share a broad range of carbohydrate substrates
A second aspect of carbohydrate metabolism that we considered was a comparison of growth on defined and complex carbon substrates (Figure 6 and Figure S4; www.fung-growth.org). It was anticipated that growth profiles could illuminate differences between pathogens with dicot and gymnosperm hosts and show correlations with their respective gene complements. In a study of polysaccharide hydrolysis activities of many fungal pathogens, King et al. [86] showed preferential substrate utilization based on
host specificity (dicot or monocot). In general D. septosporum grows more slowly on minimal control medium [87] than C. fulvum, but surprisingly overall the growth profiles of the two fungi are similar on most substrates (Figure 6 and Figure S4; Table S6) and both appear to utilize a broader range of substrates than M. graminicola (Figure 6). This is not only the case for the oligomeric and polymeric carbon substrates, requiring CAZymes for degradation, but also for monomeric carbon substrates, suggesting a diverse and efficient carbon catabolism in C. fulvum and D. septosporum. The good growth of D. septosporum on sucrose is particularly striking, suggesting that it can utilize sucrose available in apoplastic fluid during its early biotrophic colonization phase.
In terms of complex carbon sources, D. septosporum shows a slightly better capacity than C. fulvum to utlise apple and citrus pectin (Figure 6 and Figure S4). This seems to contradict the higher pectinolytic gene numbers in C. fulvum compared to D.
septosporum, but is supported by the expression of fewer C. fulvum pectinolytic genes during infection of tomato when compared to the D. septosporum pectinolytic genes during infection of pine needle (Table 6). Interestingly, good growth on pectin is also observed for M. graminicola, despite an even lower number of putative pectinases than D. septosporum. This suggests that regulation of expression is a
Table 6.Comparison of selected CAZy gene families between
C. fulvum, D. septosporum, and five other Ascomycetes.CAZy familiesa Predicted functionb Cfc Ds Mg Sn Mo Ss Bg
Biotroph Hemibiotroph Hemibiotroph Necrotroph Hemibiotroph Necrotroph Biotroph GH family FCW/energy/PCW-C/H/
HP/pectin
274 201 191 289 268 223 63
GH3 PCW/FCW 19 (15, 8) 12 (12, 12) 16 16 18 13 1
GH5 PCW/FCW 16 (12, 2) 12 (11, 12) 9 18 13 14 3
GH6 PCW-C 0 0 0 4 3 1 0
GH7 PCW-C 2 (0, 0) 1 (1, 1) 1 5 5 3 2
GH10 PCW-H 2 (2, 1) 1 (1, 1) 2 7 7 2 0
GH28 PCW-pectin 15 (8, 0) 4 (4, 4) 2 4 3 17 0
GH31 PCW-H 15 (12, 0) 10 (9, 8) 7 11 6 6 1
GH32 Energy 4 (2, 1) 2 (2, 2) 4 4 4 1 0
GH35 PCW-H 6 (3, 0) 3 (3, 1) 2 4 0 4 0
GH39 PCW-H 2 (1, 0) 0 1 1 1 0 0
GH43 PCW-HP 22 (14, 3) 11 (9, 9) 10 15 20 4 0
GH78 PCW-pectin 6 (2, 2) 1 (1, 1) 2 4 3 4 1
GH88 PCW-pectin 2 (1, 0) 0 0 1 1 0 0
GH95 PCW-pectin 2 (2, 0) 0 0 2 1 1 0
PL family PCW-pectin 9 4 3 10 5 5 0
PL1 PCW-pectin 3 (2, 0) 1 (1, 1) 2 4 2 4 0
PL3 PCW-pectin 3 (1, 0) 0 1 2 1 0 0
CE family FCW/PCW-H/HP/pectin 35 23 18 53 54 32 10
CE5 PCW-H 11 (7, 1) 4 (3, 4) 6 11 18 8 2
CBM family FCW/energy/PCW 28 24 21 77 113 65 14
CBM1 PCW 0 1 (1, 1) 0 13 22 19 0
aPredicted CAZymes were identified using the carbohydrate-active enzymes database tools (www.cazy.org). GH, glycoside hydrolases; PL, polysaccharide lyases; CE, carbohydrate esterases; CBM, carbohydrate-binding modules. Total gene numbers in these families are shown in bold. Families that are discussed in the text and differ greatly in copy number betweenCfandDsare also shown. Additional data are in Supporting Table S5.
bWhere known, CAZy functions are shown as plant cell wall (PCW) or fungal cell wall (FCW) degrading and modifying enzymes, or energy-related, with substrate preferences for PCWs of cellulose (C), hemicellulose (H), hemicellulose or pectin side-chains (HP) or pectin, using classifications as in [43].
cFungal species and their pathogenic lifestyles are shown:Cf, C. fulvum; Ds, D. septosporum; Mg, Mycosphaerella graminicola; Sn, Stagonospora nodorum; Mo, Magnaporthe oryzae; Ss, Sclerotinia sclerotiorum; Bg, Blumeria graminis. Numbers in parenthesis forCfandDsare number of genes expressed under two conditions (in culture,in planta) as described in Tables S12 and S13.
doi:10.1371/journal.pgen.1003088.t006
more dominant factor in pectin degradation by these plant pathogens than the number of pectinase-encoding genes in their genomes. In contrast, pectinase gene numbers correlate well with growth profiles of Aspergillus nidulans, A. oryzae and A. niger [88].
Compared to growth on controls lacking a carbon source, D.
septosporum also showed slightly better growth than C. fulvum on lignin. This would be consistent with the higher proportion of lignin in pine needles, estimated to be 25–30% of dry weight [89], compared to less than 10% in dicots [90]. However, due to the very slow growth of both fungi and the non-uniform growth habit of D. septosporum on these media, firm conclusions about their abilities to utilize lignin cannot be made.
Adaptations for coping with chemical and structural defences
Tomato plants produce the antimicrobial saponin, tomatine. The tomato pathogen Fusarium oxysporum produces
a-tomatinase, whichfunctions as a virulence factor as it degrades tomatine into the non- toxic compounds tomatidine and lycotetraose [91]. A gene predicted to encode
a-tomatinase, classified as a GH10 enzyme,was found in the C. fulvum genome (JGI ID 188986) but is absent from the D. septosporum genome. Another gene found only in C.
fulvum shows predicted similarity to the GH5 family enzyme hesperidin 6-O-a-L-rhamnosyl-b-glucosidase that can degrade hesperidin [77]. Hesperidin occurs most abundantly in citrus fruits [92] and is a member of the flavonoid group of compounds that is well known for its antimicrobial activity. Flavonoid-degrading enzymes such as hesperidin 6-O-a-L-rhamnosyl-b-glucosidase might enable C. fulvum to detoxify hesperidin or related compounds present in tomato.
Chemical defence molecules in pine needles include antimicro- bial monoterpenes. Thus it is expected that D. septosporum is adapted to tolerate or degrade these compounds whilst C. fulvum is not.
Recent work on the pine pathogen Grosmannia clavigera revealed several classes of genes that are upregulated in response to terpene treatment [93]. After 36 h, major classes of upregulated genes included those involved in
b-oxidation as well as mono-oxygenasesand alcohol/aldehyde dehydrogenases that may be involved in activating terpenes for
b-oxidation.A drug transporter, GLEAN_8030, was functionally analyzed and found to be required for tolerance of the fungus against terpenes, enabling G. clavigera to grow on media containing these compounds. A search for three of these genes, including GLEAN_8030, showed that both C. fulvum and D. septosporum genomes contain putative homologs and share a similar gene complement to each other (Table S7). However, since these genes have not all been functionally characterized in G.
clavigera and all are predicted to encode proteins involved in general metabolic processes, further work is required to determine the roles of the homologs found in both C. fulvum and D. septosporum.
As well as chemical mechanisms, plants employ basal structural defence mechanims including lignification of cell walls [94,95].
Due to the abundance of lignin in pine needles that block access to usable cellulose, fungal pathogens and saprophytes living on pines have a particularly challenging environment [96]. For D.
septosporum to complete its lifecycle, degradation of pine needle tissue must occur so that conidiophores bearing conidia can erupt through the epidermis (Figure 1H), which contains lignin [97].
This is in contrast to C. fulvum whose conidiophores emerge from tomato leaves through stomatal pores (Figure 1D). Thus, we investigated genes that may be involved in lignin degradation.
Some saprophytic fungi utilize oxidoreductases, particularly class-II peroxidases such as lignin peroxidases, manganese peroxidases and laccases, and a number of H
2O
2-producing enzymes, to achieve lignin breakdown [98,99]. However, the
number of genes encoding oxidoreductases in D. septosporum is no higher than those of other Dothideomycetes (C. fulvum, M. graminicola and S. nodorum) that infect plants with lower levels of lignin (Table S8). D. septosporum appears to have a similar complement of laccase genes as C. fulvum and only one distant relative of a class-II peroxidase, missing in C. fulvum, but also present in M. graminicola and S. nodorum. Interestingly, the classical Ascomycete laccases found in C. fulvum, D. septosporum and M. graminicola bear a carbohydrate- binding domain (CBM20, putative starch binding domain). This type of laccase is only found in Dothideomycetes but the significance of this novel modular structure is unclear. Brown-rot saprophytes such as Serpula lacrymans have a reduced complement of ligninolytic genes compared to lignin-degrading white-rot fungi and are proposed to initially weaken lignocellulose complexes by non- enzymatic use of hydroxyl radicals prior to enzymatic assimilation of accessible carbohydrates [81]. It is likely that D. septosporum uses a similar strategy to breach the lignin-rich components of pine needles, as complete degradation of this polymer is not required to complete its life cycle.
The secondary metabolite gene complement of C. fulvum and D. septosporum
Secondary metabolites (SMs) are important compounds for the colonization of specific ecological niches by fungi. In particular,
Figure 6. Comparative growth profiling of fungi on various carbohydrate substrates. Growth on different substrates was compared between six fungi on nine media to highlight differences.Cf,C. fulvum;Ds,D. septosporum;Mg,M. graminicola;Sn,S. nodorum;
Mo, Magnaporthe oryzae; Ss, Sclerotinia sclerotiorum. D-Glucose, D- xylose, L-arabinose and sucrose were added at a final concentration of 25 mM. Birchwood xylan, apple pectin and lignin were added at a final concentration of 1% (w/v).
doi:10.1371/journal.pgen.1003088.g006
plant-pathogenic fungi can produce non-specific and host-specific toxic SMs [100]. SMs also include mycotoxins that contaminate food and feed and are harmful to mammals [100]. The only currently known SMs produced by C. fulvum and D. septosporum are cladofulvin and dothistromin, respectively [101,102]; both compounds are anthraquinone pigments. In fungi, SM biosynthetic pathways often involve enzymes encoded in gene clusters [103] and always require the activity of at least one of four key enzymes: polyketide synthase (PKS), non-ribosomal peptide synthetase (NRPS), terpene cyclase (TC) or dimethylallyl tryptophan synthase (DMATS) [104]. It has been suggested that loss of SM biosynthetic pathways is associated with biotrophy [44], thus we searched for SM gene pathways in both genomes. Surprisingly, the biotroph C. fulvum has twice the number of key SM genes (23 in total) compared to the hemibiotroph D.
septosporum (11 in total) (Table 7), of which 14 and 9, respectively, are organized into gene clusters along with other SM-related genes. The numbers of key SM enzyme-encoding genes are comparable to those of M. graminicola, but are lower than those in most other sequenced Dothideomycetes [42]. Like all Ascomycetes [105], the majority of key SM enzymes in C. fulvum and D. septosporum are PKSs, NRPSs and hybrid PKS-NRPSs. Annotation of all key SM genes was manually checked and two truncated (Pks4 and Nps1) and five pseudogenized (Pks9, Hps2, Nps5, Nps7 and Nps10) genes were found in the C. fulvum genome, while all D. septosporum genes except Pks4 (truncated) are predicted to encode functional enzymes. Overall, the number of predicted functional pathways suggests that C. fulvum and D.
septosporum can produce at least 14 and 10 different SMs, respectively.
Surprisingly, only three of the key SM genes are predicted to belong to biosynthetic pathways shared between the two species (Table S9) suggesting a diverse SM repertoire. This is much lower than expected given the overall level of similarity in gene content between the two genomes, and suggests that this SM repertoire is under strong selection. The three common genes are predicted to be involved in production of a pigment related to melanin (Pks1), a siderophore (Nps2) and dothistromin (PksA) based on similarities to other characterized genes. In C. fulvum, the three other functional non-reducing PKS enzymes are candidates for production of cladofulvin.
The genomic locations of the 11 biosynthetic SM genes in D.
septosporum do not show any enrichment at sub-telomeric positions, as reported for Aspergillus spp. and Fusarium graminearum [106,107], or near putative centromeres (Figure 3). However, 8 out of the 11 genes are located on chromosomes smaller than 2-Mb (chromo- somes 8 to 12; Figure 3). The genomic regions immediately surrounding all 11 D. septosporum SM genes are conserved in the C.
fulvum genome, although 8 of them lack the key SM gene itself and, sometimes, putative accessory genes also (Figure S5). Reciprocally, only 9 C. fulvum SM genomic regions out of 23 are conserved in D.
septosporum with 6 of these lacking the key SM gene, suggesting either gain or loss of SM genes has occurred. For two of the regions where flanking genes are conserved but SM gene(s) are missing in C. fulvum (regions corresponding to those surrounding Pks3 and Nps3 in D. septosporum), the presence of repeats suggests that SM gene loss may have occurred in C. fulvum (Figure S5). The C. fulvum-specific SM loci Pks5, Pks6, Nps5/Dma1 and Nps9 include many transposable elements and genes that have similarity to genes scattered in the D. septosporum genome, often on the same chromosome, leading to the hypothesis that these SM loci were assembled by gene relocation as recently proposed for the fumonisin gene cluster in F. verticillioides [108].
Dothistromin toxin genes are present in both genomes Analysis of the D. septosporum 1.3-Mb chromosome 12 revealed that the three previously identified mini-clusters of dothistromin genes [38] are widely dispersed, confirming fragmentation of this gene cluster (Figure 3 and Figure 7). Candidates for additional dothistromin genes, previously predicted based on aflatoxin pathway genes [39], are also present. Although three of these genes (OrdB, AvnA, HexB) are located in the published VbsA mini- cluster, the others are dispersed over different regions of chromosome 12 as shown in Figure 7. The end of the Nor1 gene cluster (Nor1, AdhA, VerB) is less than 10-kb from one predicted telomere, whilst Ver1 (previously called dotA [35]) is only 81-kb from the other telomere. As expected, a gene similar to the aflatoxin AflR regulatory gene is present and, like in aflatoxin- producing species of Aspergillus, is divergently transcribed with an adjacent AflJ regulatory gene candidate. Functional analysis of these genes is in progress.
Although C. fulvum is not known to produce dothistromin, the complete set of predicted dothistromin genes is present in its genome, encoding proteins with amino acid identities ranging from 49% (AflJ) to 98% (Ver1) when compared with those of D.
septosporum (Table S10). The arrangement of predicted dothis- tromin genes in C. fulvum reveals a high level of synteny with some rearrangements. With the exception of the Ver1 gene cluster, the mini-clusters contain the same genes in the same orientations in the two species (Figure 7A). The three mini-clusters on C. fulvum scaffold 130775 are much closer together than in D. septosporum, but are still separated from each other by considerable distances (approximately 24-kb between Est1 and the VbsA gene cluster,
Table 7.
Key secondary metabolism genes in Ascomycete genomes.
Fungal species Lifestyle PKS NRPS Hybrid TC DMATS Total
Cladosporium fulvum Biotroph 10 10 2 0 1 23
Dothistroma septosporum Hemibiotroph 5 3 2 0 1 11
Mycosphaerella graminicola Hemibiotroph 11 6 2 1 0 20
Stagonospora nodorum Necrotroph 22 10 2 2 2 38
Magnaporthe oryzae Hemibiotroph 22 8 10 3 3 46
Fusarium graminearum Necrotroph 13 12 2 3 0 30
Aspergillus nidulans Saprophyte 26 10 2 5 2 45
Neurospora crassa Saprophyte 6 3 1 1 1 12
Numbers of predicted polyketide synthase (PKS), non-ribosomal peptide synthetase (NRPS), hybrid PKS-NRPS (Hybrid), terpene cyclase (TC) and dimethylallyl tryptophan synthase (DMATS) genes are shown. Data are from this study and from Collemare et al. 2008 [105].
doi:10.1371/journal.pgen.1003088.t007
